The Vertebrate Primary Cilium in Development, Homeostasis, and Disease (original) (raw)

. Author manuscript; available in PMC: 2011 Jan 5.

Abstract

Cilia are complex structures that have garnered interest because of their roles in vertebrate development and their involvement in human genetic disorders. In contrast to multicellular invertebrates in which cilia are restricted to specific cell types, these organelles are found almost ubiquitously in vertebrate cells, where they serve a diverse set of signaling functions. Here, we highlight properties of vertebrate cilia, with particular emphasis on their relationship with other subcellular structures, and explore the physiological consequences of ciliary dysfunction.

Cilia are polarized structures that appeared early in the evolution of eukaryotes. Although initially studied for their roles in cell and/or fluid propulsion, it is now known that cilia serve a variety of sensory functions in both unicellular and multicellular organisms. This expanding view of ciliary roles is coincident with an increased appreciation of both their structural complexity and their content diversity. Whereas original estimates placed the number of proteins at the basal body and ciliary axoneme at 150 and 250, respectively (Dutcher, 1995), the recent assessment of ten comparative genomics and proteomics data sets enriched for basal body and ciliary proteins suggests that the vertebrate cilium may require up to ~1000 different polypeptides for its function (Gherman et al., 2006, and http://www.ciliaproteome.org). Integration of an additional proteomics study reporting the protein content of the connecting cilium and outer segment of the mouse photoreceptor potentially augments this number even further (Liu et al., 2007a). Yet, it is not clear what minimal fraction of those proteins is required in situ as opposed to other cellular sites. The projected complexity of the total ciliary protein complement reflects the multifaceted roles that cilia play in vertebrates. Here, we provide a perspective of our current understanding of ciliary biology, highlighting examples of ciliary roles and exploring the consequences of ciliary dysfunction.

Ciliary Structure in Vertebrates

Much of our understanding of ciliary constituents is based on observations made from flagella isolated from the green alga Chlamydomonas (Dutcher, 1995). The archetypical cilium extends from the apical membrane of cells and relies on a microtubule scaffold (Figure 1A). Surrounded by a plasma membrane, the ciliary axoneme begins as a radial array of microtubule triplets at its cellular anchor, the basal body. The common ciliated eukaryotic ancestor also contained a set of inner microtubules, known as the “central pair,” which has either been maintained during evolution in the “9+2,” or lost in the “9+0” configurations. Although the majority of motile cilia possess the 9+2 arrangement, and most nonmotile cilia have the 9+0 configuration, notable exceptions include motile 9+0 ependymal cilia in the central canal of the zebrafish spinal cord (Kramer-Zucker et al., 2005; Figure 1B) or immotile 9+2 cilia in frog olfactory epithelium (Reese, 1965).

Figure 1. Ciliary Structure in Vertebrates.

(A) Microtubule structure of the vertebrate cilium. Cilia are tethered to the apical aspect of the cell at the basal body, surrounded by pericentriolar material. Nine radially organized microtubule triplets protrude from the basal body to the transition zone, and then extend as microtubule doublets in the ciliary axoneme. Electron micrograph images of each portion of the cilium are shown to the left. Images are from Kramer-Zucker et al. (2005) and Feistel and Blum (2006), reprinted with permission from John Wiley & Sons, Inc. from Developmental Dynamics, Vol. 235, 2006, p. 3348–3358. Copyright (2006) John Wiley & Sons, Inc., and Fromherz et al. (2004), reproduced with permission from Journal of Cell Science.

(B) Diversification of ciliary architecture in vertebrate species. Whereas invertebrate models such as C. elegans and D. melanogaster have cilia restricted to certain cell types, nearly all vertebrate cells are ciliated. Examples shown from zebrafish, mouse, and rabbit demonstrate the possible expansion of ciliary roles in vertebrates. This expansion is exemplified by populations of cilia in vertebrate tissues that are architecturally heterogeneous, such as the rabbit notochordal plate and the mouse kinocilium. Moreover, there are exceptions to the general association between the central microtubule pair and motile cilia, such as motile ependymal cilia (9+0) in the zebrafish spinal cord and nonmotile sensory kinocilia (9+2) in the mouse inner ear.

Intraflagellar Transport

Our current comprehension of intraflagellar transport (IFT) is based on experiments carried out in Chlamydomonas and subsequently in C. elegans (for a recent review, see Scholey, 2008). Given that protein synthesis is not known to occur at the cilium, proteins travel to their final destination by the dynamic cooperation of molecular motors and protein scaffolds. Anterograde IFT is mediated by the heterotrimeric kinesin-2 motor, and cytoplasmic dynein facilitates retrograde IFT. In cooperation with these motors, “core” protein complexes known as IFT particles A (retrograde) and B (anterograde) are thought to bind to protein cargo through protein interaction domains and in vertebrates the complexes consist of at least six and ten different proteins respectively (Scholey, 2008) (Figure 2).

Figure 2. Vesicular Transport and Intraflagellar Transport.

Accumulating evidence indicates that vesicular transport of ciliary proteins from the trans-Golgi network is critical for proper cilium formation and may be facilitated, at least in part, by the intraflagellar transport (IFT) particle protein IFT20. Furthermore, Rabin8 interacts directly with Bardet-Biedl Syndrome protein BBS1, complexed with the BBSome in the basal body. Rabin8 is required for Rab8 GDP/GTP exchange. Rab8-GTP is proposed to be transported in vesicles to the base of the cilium, where it may dock with the ciliary membrane and/or the IFT complex. Upon targeting to the base of the cilium, ciliary proteins are transported toward the ciliary tip with the kinesin-2 motor in cooperation with IFT complex B proteins (listed on the left; shown in orange). TRAF3IP1/elipsa has been shown to function as an accessory anterograde IFT protein that binds directly with IFT20. Recycling of proteins toward the basal body is mediated by a cytoplasmic dynein and IFT complex A proteins (listed on the right; shown in blue).

A combination of biochemical and in vivo studies on IFT mutants has catalyzed the discovery of a number of critical roles for IFT and cilia in general with regard to vertebrate physiology (see http://v3.ciliaproteome.org/pdf/Vertebrate%20ciliary%20mutants.pdf). For example, the cooperative sensory and motile roles of cilia in the embryonic node in mouse and the Kuppfer’s vesicle in zebrafish, which are abolished in a variety of IFT mutants, have highlighted the critical role of cilia in the early events in left-right axis determination (Hirokawa et al., 2006; Tabin, 2006). Likewise, defects in either IFT particle assembly or receptor targeting to the ciliary membrane are linked to defective intracellular Ca2+ responses to mechanical stimuli (Yoder, 2007), and the biophysical properties of cilia are important in the dynamics of ciliary motility (Marshall and Kintner, 2008). As each of these topics have been reviewed in depth recently, the following sections focus on recent advances and newly emerging areas of ciliary research.

Cell Biology of Primary Cilia

Cilia, Golgi, and Vesicular Transport

Emerging clues suggest that cilia have specific, and potentially physiologically relevant, interactions with other intracellular compartments. One of the cellular organelles found consistently in the proximity of the primary cilium and the basal body is the Golgi apparatus. In the 1960s, the availability of electron microscopy led to the observation that the Golgi network localizes close to the basal body, and ciliogenesis follows the flattening of a vesicle to the distal end of the centriole destined to form the basal body of the newly formed cilium (Sorokin, 1964). In later stages of ciliogenesis, the ciliary sheath forms out of the initial primary ciliary vesicle (Sorokin, 1964). When electron microscopy was complemented with confocal laser scanning microscopy, the characterization of spatial relationships became more accessible. In chondrocytes and aortic smooth muscle cells, the primary cilium, the Golgi, and the nucleus are consistently found in proximity to each other (Poole et al., 1997), which has since been observed in other cell and tissue types, likely highlighting a functional, but as yet unknown, link between these organelles.

The relationship between the primary cilium and Golgi along with sequence homology between IFT proteins and coat protein I (COPI) and clathrin-coated vesicle components (Jekely and Arendt, 2006) suggest evolutionary roots of the primary cilium in vesicle transport. Indeed, the structural correlation between the primary cilium and the Golgi is exemplified by the localization of Xklp3, a Xenopus subunit of the kinesin-2 complex, on vesicles of the intermediate compartment (IC) between the endoplasmic reticulum and the Golgi apparatus (LeBot et al., 1998). This suggested relationship has been highlighted more recently: IFT20, a component of the IFT particle B complex, localizes to both the Golgi and the primary cilium (Follit et al., 2006) (Figure 2). The role of IFT20 is unlikely to overlap with kinesin-2 because, at least in human retinal pigment epithelial (RPE) cells, IFT20 depletion suppresses ciliary assembly but does not affect either the integrity of the Golgi complex or the localization of kinesin-2 on Golgi vesicles. Nonetheless, the question still remains whether these data reflect two independent (one ciliary, one Golgi-specific) or interlinked roles for this protein.

A series of observations have begun to assemble a model in which vesicular transport (perhaps from the trans-Golgi network) is necessary for ciliogenesis and potentially also important for protein targeting to the transition zone of mature cilia. The zebrafish coiled-coil polypeptide elipsa is a binding partner of Ift20 and Rabaptin5, a regulator of endocytosis, which in turn interacts with Rab8, a small membrane-associated GTPase (Omori et al., 2008). Notably, Rab8 is known to participate in rhodopsin transport in photoreceptors by regulating docking and fusion of rhodopsin-bearing post-Golgi membranes (Moritz et al., 2001), and loss of Rab8 results in an accumulation of vesicles at the base of the photoreceptor connecting cilium. Moreover, Rab8a has been shown to bind directly to cenexin/ODF2, a centrosomal and basal body component (Yoshimura et al., 2007). In addition, the recently identified BBSome, a complex of seven of the fourteen known causative Bardet-Biedl Syndrome (BBS) proteins, provides more evidence for a ciliary role of Rab8, as it is thought to bind to the C terminus of Rabin8, the guanosyl exchange factor specific for Rab8 (Nachury et al., 2007).

Cell Polarity and Ciliogenesis

The primary cilium is a polarized structure. It is therefore not surprising that several independent observations now support an intimate link between the primary cilium and the establishment and maintenance of cell polarity.

The formation of cell and tight junctions is important for cellular polarization and the subsequent formation of polarized structures such as the cilium; polarity complexes localize to cellular junctions, where several basal body and ciliary components are observed as well, such as inversin (Nurnberger et al., 2002) (Figure 3A). The reverse is also true, in that several factors determining cell polarity localize to both the tight junctions and the primary cilium, such as the complex consisting of the partitioning-defective protein 3 (Par3), partitioning-defective protein 6 (Par6), and atypical protein kinase Cζ (aPKCζ) (Fan et al., 2004) (Figure 3A). However, it is not clear whether these data indicate a functional link between cell and tight junctions or unrelated functions of the proteins dependent on their cellular context.

Figure 3. Control of Ciliogenesis.

(A) Ciliary proteins localize to cell junctions and polarity proteins localize to the primary cilium. Inversin localizes to three separate cellular protein pools: the primary cilium, cell junctions, and the nucleus. Two different polarity complexes, Par3/Par6/aPKCζ and CRB3/PATJ1/PALS, as well as the polarity protein 14-3-3η, localize to cell junctions and the primary cilium. Galectin-3 also marks a membrane region of increased lipid density surrounding the cilium.

(B) The transcription factors Noto, FoxJ1, and Rfx3 play a role in ciliogenesis. Noto acts downstream of Foxa2 and T (brachyury) and upstream of FoxJ1 and Rfx3. Embryonic node and nodal cilium in E7.5 wild-type and _Noto-_deficient mice (Beckers et al., 2007) reveal structurally abnormal and stunted cilia. Images are reproduced with permission from PNAS, Vol. 104, p. 15765–15770. Copyright (2007) National Academy of Sciences, U.S.A. Scanning electron micrographs of explanted trachea show multiciliated cells covering most of the apical surface in wild-type trachea. These are absent from mice that are Foxj1 deficient, whereas primary cilia are unaffected. Scanning micrographs of embryonic nodes of Theiler stage 11c of wild-type and Rfx3 deficient mice. Cilia in Rfx3 deficient mice are shorter and misoriented compared to the wild-type (Bonnafe et al., 2004). Images reproduced from Molecular and Cellular Biology, 2004, Vol. 24, p. 4417–4427, with permission from the American Society for Microbiology.

(C) A complex of Cep97 and CP110 suppresses ciliogenesis throughout the cell cycle. Mitotic entry is regulated by the G2/M transition through CDC2-Cyclin B, which activates several kinases, including the Nek family and AurA. In murine inner medullary collecting duct (IMCD3) cells, NEK5 localizes to the centrosome and the distal tip of the basal body. In human retinal pigment epithelial cells, a pool of AurA localizes to the basal body.

Does the primary cilium actively participate in the establishment of apical-basolateral polarity, or is it the outcome of such a process? As an apical structure, it is most likely a product of the polarization process. Consistent with this notion, perturbations in the polarizing processes result in defects in ciliogenesis. Loss of a component of the apical transport machinery, phosphatidylinositol-4-phosphate adaptor protein 2 (FAPP2) leads to delayed cilia formation in adherent Madin-Darby canine kidney (MDCK) cells and abolishes cilia formation in MDCK cysts (Vieira et al., 2006). In FAPP2-depleted cells, tight junctions are fully functional, but localization of galectin-3, a subapical marker, indicates a polarity defect. Moreover, loss of FAPP2 leads to a transient accumulation of subapical transport vesicles in the vicinity of the microtubule-organizing center and to a shift in the balance of apical and basolateral membrane lipid rafts. Subsequently, an RNA interference (RNAi) screen in MDCK cells identified several candidate apical transport proteins involved in ciliogenesis or regulation of ciliary length (Torkko et al., 2008).

The establishment of cell polarity in epithelial cells thus appears to be a prerequisite for ciliogenesis, and apical transport proteins fulfill dual roles in cell polarization and cilia assembly. It is important to note, however, that mesenchymal cells are ciliated even though they lack apicobasal polarity. On the other hand, the presence of the cilium might itself exert an effect in maintaining cell polarity. Disruption of ciliary components such as KIF3A or polaris/IFT88 leads to cell polarity defects: suppression of Kif3a leads to both loss of cell polarity and defective ciliogenesis in vitro (Fan et al., 2004; Lin et al., 2003). In kidneys of mice with a hypomorphic mutation in Tg737/Ift88, the localization of the epidermal growth factor receptor (EGFR), which in cells of wild-type mice is typically basolateral, extends into the apical membrane of renal cysts (Taulman et al., 2001). Taken together, these data suggest several alternatives. First, we cannot exclude the possibility that proteins such as KIF3A have nonciliary roles, disruption of which leads to the observed polarity defects. For example, KIF3A also plays a role in spindle formation and mitosis (Haraguchi et al., 2006). At the same time, it is reasonable to speculate that the loss of the primary cilium can lead to the impairment of the establishment or maintenance of apical polarity. It will be interesting, in this regard, to examine the behavior, assembly, and stability of the Par3/Par6/aPKCζ complex in a series of ciliary mutants, particularly those that have functional but not overt structural defects in ciliary assembly and maintenance.

Ciliary Dynamics

Centrosomes are the anchoring structures for both cilia, in the form of the basal body, and mitotic spindles. Although basal bodies and centrosomes on one hand and mitotic spindles and centrosomes on the other can easily interconvert, there are no reports of cells with both cilia and mitotic spindles. In fact, primary cilia are regarded as postmitotic structures of quiescent cells. Ciliary dynamics thus appear to be precisely coordinated with cell cycle progression; the molecular cues triggering ciliary assembly and disassembly, however, are understood insufficiently.

The known cues for ciliary assembly seem to act through derepression, indicating that the cellular default state would be active ciliary assembly: a complex of two centrosomal proteins, Cep97 and CP110, likely acts as a suppressor of ciliogenesis (Spektor et al., 2007); depletion of either Cep97 or CP110 in mammalian cells leads to mislocalization of the other binding partner and either monopolar or multipolar spindle pole formation. The concurrent suppression of Cep97 and CP110 messages results in assembly of cilia-like structures containing well-established ciliary markers such as glutamylated and acetylated tubulin, polaris/IFT88, and polycystin-2 (PC2), as well as centriole markers including centrin in cells that had not exited the cell cycle (Figure 3C). Because centrin is contained over the entire length of the structures, it has been argued that these are not cilia but rather elongated centrioles (Keller et al., 2008). In addition, the increased presence of binucleated cells suggests a cytokinesis defect likely connected to aberrant mitotic spindle formation. Overexpression of CP110 in serum-starved quiescent cells suppressed the formation of primary cilia without perturbation of cellular quiescence, further indicative of a repressive function on ciliogenesis (Spektor et al., 2007). During G0, CP110 is not expressed, indicating that ciliation might be initiated through a yet unknown mechanism triggering transcriptional repression of CP110.

Recent evidence suggests the presence of a CP110 population complexed by CEP290/NPHP6 that is separate from other complexes involved in cell cycle progression or ciliation, such as Cep97/CP110 (Tsang et al., 2008). CEP290 localizes to the centrosome and both daughter and mother centrioles, but does not seem to play a role in centrosome function, because cell cycle progression and spindle formation are unaffected by its loss. However, interaction of CP110 and CEP290 is required for suppression of ciliary assembly, indicating that the centrosomal CEP290 population may be targeted to the structure that will give rise to the basal body. Yet, depletion of CEP290 leads to loss of ciliogenesis (Graser et al., 2007), indicating that further experiments are needed to resolve the functions of CEP290.

At the other end of the ciliary life cycle, retraction of the primary cilium and re-entry into mitosis are tightly coordinated, and the details of this process are beginning to be illuminated. Ciliary disassembly is not a prerequisite for cell cycle entry, because loss of CP110 leads to ciliary formation in nonquiescent cells (Spektor et al., 2007). Intriguingly, two of the kinases that regulate mitotic entry are involved in retracting the cilium, suggesting that the G2/M transition is tightly coordinated with ciliary disassembly (O’Connell et al., 2003): In Chlamydomonas reinhardtii, a genetic screen for deflagellation mutants identified FA2, encoding a member of the Nek family of kinases, which plays a role both in basal body/centriole associated microtubule severing and in cell cycle progression. Interestingly, in mice, mNek1, mNek8, and mNek5/Fa2p are associated with the basal body and centrioles in a cell cycle-dependent manner (Mahjoub et al., 2005) (Figure 3C), and perturbations in Nek1 and Nek8 cause polycystic kidneys in mice and zebrafish (Liu et al., 2002; Upadhya et al., 2000).

Another kinase that regulates ciliary disassembly is Aurora A (AurA), a homolog of Chlamydomonas aurora/Ipl1p-like protein kinase (CALK) (Pan et al., 2004; Pugacheva et al., 2007). Interaction of AurA with scaffolding protein HEF-1 at the basal body activates AurA and triggers ciliary disassembly through phosphorylation/activation of histone deacetylase 6 (HDAC6), a microtubule deacetylase (Pugacheva et al., 2007) (Figure 3C), suggesting that ciliogenesis and ciliary disassembly are tightly coordinated with, but are not integral components of, the cell cycle. Although the cilium is a characteristic of quiescent cells, it does not inhibit mitosis, and disruption of the cilium does not lead to widespread proliferative phenotypes. The precise mechanism by which cilium disassembly is synchronized to cell cycle progression will have to be addressed in more detail, particularly the time at which it occurs. One hypothesis is that CDC2-CyclinB directly activates retraction of the primary cilium (O’Connell et al., 2003).

Transcriptional Regulation of Ciliation

Ciliogenesis is an intricate, coordinated process involving dozens, and possibly hundreds, of proteins. Studies in Chlamydomonas have demonstrated that a host of genes are upregulated after deflagellation (Li et al., 2004). However, little is known about the ciliogenesis circuit in vertebrates, or indeed the regulatory processes that might specifically regulate the various architectural and functional types of vertebrate cilia.

The homeobox gene Noto regulates the formation of nodal cilia downstream of Foxa2 and T (Abdelkhalek et al., 2004). Mice lacking Noto show defects in the caudal notochord and laterality, varying from heterotaxy to situs inversus or situs solitus. Although cilia are present in the posterior notochord, they are both reduced in number and shorter in length, with partially disorganized or incomplete microtubular structures (Beckers et al., 2007) (Figure 3B) In addition, expression levels of the transcription factors Rfx3 and FoxJ1, each of which is critical to ciliogenesis, are reduced or completely abolished, suggesting that Noto acts upstream of both factors (Beckers et al., 2007). Mice deficient in Rfx3 show left-right asymmetry defects (Bonnafe et al., 2004) (Figure 3B), and a C. elegans ortholog of Rfx3, daf-19, regulates the expression of a number of ciliary genes (Efimenko et al., 2005; Li et al., 2004). Likewise, mice deficient in Foxj1 die either in utero or in the early neonatal period because of hydrocephalus or heterotaxia, and they lack respiratory cilia (Brody et al., 2000; Chen et al., 1998). Subsequent studies have shown that _Foxj1_-deficient mice have primary 9+0 cilia but lack motile 9+2 cilia, implicating FoxJ1 in motile but not primary ciliogenesis, although it is not clear whether the primary cilia function normally (Zhang et al., 2004) (Figure 3B). Recently, the role for FoxJ1 in motile cilia formation has been expanded from mice to Xenopus and zebrafish (Stubbs et al., 2008; Yu et al., 2008). This suggests that overall ciliary architecture is regulated and maintained by similar transcriptional mechanisms regardless of cilia subtypes, because Noto, which controls length, number, and microtubular structure of all cilia, acts upstream of FoxJ1, which specifically regulates formation of 9+2 cilia.

Although we know some of the key players in the transcriptional activation of ciliogenesis, we do not know the triggering events involved in cilia formation. One possible exception, at least for the formation of motile cilia in multiciliated cells, is the implication of a role for notch3 and jagged2 in the regulation of cell fate in the epithelial tubules of the zebrafish pronephros (Liu et al., 2007b; Ma and Jiang, 2007). Suppression of either signaling component expands ciliary gene expression and leads to a greater number of multiciliated cells in the pronephros, whereas ectopic expression of notch1a represses the differentiation of multiciliated cells.

The Primary Cilium in Signal Transduction

Regulation of Canonical and Noncanonical Wnt Signaling

In addition to apicobasal polarity, cells also establish a plane of polarity distinguishing proximal from distal ends, a process regulated by planar cell polarity (PCP) signaling. In vertebrates, PCP signaling represents a subset of noncanonical Wnt signaling, and hallmarks of defective noncanonical Wnt signaling include impaired convergent extension movements during gastrulation, neural tube closure failure, and disorganization of stereocilia in the mouse inner ear (Veeman et al., 2003). Extracellular Wnt stimulates the signal transduction cascade by binding to a complex of the Frizzled (Fz) receptor and the low-density lipoprotein receptors LRP5 or LRP6. In humans, there are 19 Wnt ligands, ten Fz receptors, and numerous Wnt effectors, acting in a context- and tissue-dependent manner (Figure 4A). The signal is transmitted by Disheveled (Dvl), which localizes to two separate pools within the cell depending on the signaling context. Nuclear localization of Dvl is necessary for the β-catenin-dependent or canonical Wnt signaling pathway, which results in transcriptional activation of genes under the control of T cell-specific transcription factor/lymphoid enhancer factor-1 (TCF/LEF-1)-responsive elements (Itoh et al., 2005). In the context of noncanonical Wnt signaling, Dvl is commonly localized to the plasma membrane (Axelrod et al., 1998; Rothbacher et al., 2000; Seto and Bellen, 2004).

Figure 4. The Primary Cilium in Wnt and Shh Signaling.

(A) In the absence of Wnt stimuli, β-catenin is constitutively phosphorylated by the β-catenin destruction complex consisting of Axin, APC, and GSK3β. Phosphorylated β-catenin is targeted for degradation. Wnt targets are repressed by a complex of TCF/LEF1 and TLE. In canonical Wnt signaling, the ligand binds to a complex of the Frizzled receptor and LRP5/6 coreceptor, which then binds to Axin and Dishevelled (DVL), leading to stabilization of β-catenin in the cytoplasm. β-catenin migrates into the nucleus, replaces TLE, and activates transcription ofβ-catenin/TCF/LEF1-responsive genes. In noncanonical signaling, activated DVL is targeted to the membrane and activates downstream targets.

(B) Effects of ciliary and basal body disruption on Wnt signaling. In ciliated cells, noncanonical Wnt signals antagonize canonical Wnt signaling, leading to proteasomal β-catenin degradation and membrane targeting of DVL. In unciliated cells, canonical Wnt signaling stabilizes cytoplasmic β-catenin and DVL, leading to increased nuclear levels of both DVL and β-catenin, initiating transcription of TCF/LEF1-responsive genes. Disruption of ciliary or basal body components leads to loss of noncanonical Wnt signaling and stabilization of both DVL and β-catenin in the cytoplasm and nucleus, resembling the status of nonciliated cells.

(C) In the absence of sonic hedgehog (Shh) ligand, Patched (Ptch) represses Smoothened (Smo). Repressive forms of the Gli proteins bind to the promoter regions of Shh targets and inhibit transcription. Stimulation with Shh ligand recruits Smo and Ptch1 to the primary cilium. Gli2 and Gli3 are localized to both the cilium and the nucleus, and in response to the ligand stimulus they are proteasomally processed into their activator Gli2/3A isoforms, activating transcription of Shh targets.

(D) Differential role of ciliary and basal body proteins in Gli2/3 processing. Perturbation of anterograde intraflagellar transport (IFT) leads to loss of Gli2 and Gli3 processing and Shh signaling. Loss of structural integrity of the primary cilium by disruption of Arl13b leads to constitutively active Gli2, but leaves Gli3 unaffected. Loss of retrograde IFT triggers both Gli2 and Gli3 proteasomal activation along with transcriptional upregulation of Gli3. Finally, disruption of the basal body does not affect Gli2 processing but increases both expression and proteasomal activation of Gli3.

Several studies have implicated ciliary and basal body proteins in the regulation of Wnt signaling: Inversin (Inv) interacts with Dvl and targets the cytoplasmic fraction of Dvl for degradation (Simons et al., 2005). Suppression of Xinv in Xenopus embryos results in defects in convergent extension, suggesting that Inversin acts as a switch required for noncanonical Wnt signaling and suppression of β-catenin activity. Although these experiments showed that Inv regulates the balance of canonical and noncanonical Wnt signaling, it was not clear which cytoplasmic population of Inv—separate protein pools are associated with the cilium, adherens junction, and nucleus—would be involved. The BBS proteins, most of which localize specifically to the basal body, provide further insight. Both mouse and zebrafish BBS models manifest symptoms typical of defective PCP signaling. Moreover, studies in Bbs models show a genetic interaction of BBS genes with core PCP genes, suggesting that basal bodies are involved in PCP signaling (Gerdes et al., 2007; Ross et al., 2005). Concordant with the implication of Inversin in the balance between canonical and noncanonical Wnt signaling (Simons et al., 2005), zebrafish bbs morphants show both defects in convergent extension indicative of impaired noncanonical Wnt signaling and expanded expression domains of β-catenin transcriptional targets. Depletion of BBS proteins in vitro results in an augmented response to Wnt3a (Gerdes et al., 2007).

Another study investigated the role of three different ciliary and basal body proteins in β-catenin-dependent Wnt signaling: Kif3a, Ift88, and Ofd1 (Corbit et al., 2008). Loss of Kif3a in mice leads to enhanced β-catenin-dependent transcriptional activation on embryonic day E9.0. Embryonic fibroblasts from both Kif3a and orpk mutant mice, as well as _Ofd1_-deficient embryonic stem cells (see http://v3.ciliaproteome.org/pdf/Vertebrate%20ciliary%20mutants.pdf), are hyperresponsive to Wnt3a through the canonical Wnt pathway.

Both studies reveal an inhibitory role of the primary cilium on the canonical Wnt signaling pathway. Loss of ciliary or basal body components leads to hyperresponsiveness to external canonical Wnt stimuli (Corbit et al., 2008; Gerdes et al., 2007) at the expense of noncanonical Wnt signaling (Gerdes et al., 2007) (Figure 4B).

Accumulating evidence also suggests some planar polarity components are necessary for ciliogenesis. Suppression of Inturned (Xint) and Fuzzy (Xfy) during Xenopus development affects ciliogenesis, and the observed Shh and PCP signaling defects of Xint and Xfy morphants are consistent with the general lack of cilia (Park et al., 2006). In _Xint_-depleted cells, microtubular structures resembling ciliary axonemes are formed, but the actin network orienting and organizing the centrioles as the ciliary base is missing. Given that int and fy were identified originally as genes in Drosophila that encode planar polarity effector proteins (Adler et al., 2004), the lack of ciliogenesis in Xint and Xfy morphants could implicate a role of planar polarity signaling in centriole migration and thus indirectly in ciliogenesis. However, although core PCP polarity proteins are required for the asymmetric localization of other planar polarity proteins, Inturned and Fuzzy do not affect the asymmetric localization of core PCP proteins (Adler et al., 2004). The reciprocity between ciliary function and noncanonical Wnt signaling is also reflected in the targeted disruption of Ift88 in the developing mouse cochlea, causing misorientation of kinociliary basal bodies and thus stereociliary bundles, whereas core PCP proteins localize normally (Jones et al., 2008). This suggests that ciliary and basal body integrity are critical for the correct translation of polarized, morphogenetic cues.

Evidence for an involvement of the PCP signaling pathway in ciliogenesis comes from zebrafish duboraya (dub) morphants, which show defects both in primary ciliary assembly and left-right patterning (Oishi et al., 2006). Importantly, the dub phenotype is replicated by suppression of frizzled-2 message, and suppression of the noncanonical Wnt signaling pathway is characterized by a misorganization of the actin skeleton (Oishi et al., 2006). The potential conflict between the involvement of cilia for the balance between canonical and noncanonical Wnt signaling pathway on one hand and the requirement of noncanonical Wnt signaling for proper ciliogenesis on the other will likely be resolved when the actual signaling cascades in a time- and tissue-specific context are identified.

Hedgehog Signaling

In mammals, the family of Hedgehog (Hh) signaling proteins consists of three different pathways governed by Indian hedgehog (Ihh), Desert hedgehog (Dhh), and Sonic hedgehog (Shh) ligands. The Hh ligand binds to the Patched (Ptch) receptor (two in mammals), which then releases repressed Smoothened (Smo) and by doing so activates downstream signaling components, including the Glioma (Gli) proteins (three in mammals) (Lum and Beachy, 2004; Hedgehog Signaling Database, http://hedgehog.sfsu.edu) (Figure 4C).

Several independent lines of evidence have demonstrated a role of the primary cilium in Hh signaling. Initially, a screen for modulators of mouse embryonic patterning identified two mutants, wimple (wim) and flexo (fxo), with characteristic Shh defects, including neural tube closure defects, abnormal brain morphology, and preaxial polydactyly (Huangfu et al., 2003). The ethylnitrosourea (ENU)-induced mutations were mapped to two IFT genes, Ift172 (wim) and Ift88/polaris (fxo), and a third ciliary transport mutant deficient for Kif3a had similar defects in floor plate specification; all three mutants showed reduced Shh signaling. Subsequently, Smo was found to localize to the primary cilium in the mouse embryonic node, which is involved in both left-right determination and floor plate induction (Corbit et al., 2005). Upon Shh stimulation, both Smo and Ptch1 are recruited to the cilium both in vitro and in vivo, where Ptch1 binds to Shh and then leaves the cilium, possibly by internalization (Rohatgi et al., 2007). Downstream effectors of the Hedgehog signaling pathway, Gli2 and Gli3, also localize to the primary cilium of mesenchymal and ectodermal cells of the developing limb bud (Haycraft et al., 2005). Disruption of IFT88/polaris leads to loss of function of both Gli2 and Gli3, suggesting a role of the cilium in processing and function of Gli2 and Gli3, but not Gli1, which activates target genes normally in IFT88-deficient cells.

Several lines of evidence suggest a differential role of ciliary/basal body proteins in Gli2/3 processing (Figure 4D). First, mouse mutants with disrupted IFT particle B genes (such as Ift52, Ift57, and Ift88) (Haycraft et al., 2005; Houde et al., 2006; Huangfu et al., 2003; Liu et al., 2005) exhibit phenotypes characteristic of loss of Shh signaling implicating anterograde IFT in proper Smo/Ptch1 localization. Second, in hennin (hnn) mutant mice, which harbor a mutation in the gene encoding the Arf-family GTPase Arl13b (Caspary et al., 2007), and whose cilia are shortened and have a defect in the axoneme, Gli3 repressor activity is unaltered compared to wild-type mice. However, Gli2 and possibly Gli3 are active ectopically, albeit at low levels, indicating that ciliary architecture plays a role in Gli2, but not necessarily Gli3, processing and function (Caspary et al., 2007). Third, the alien (aln) mouse, harboring a null mutation in the retrograde transport protein Ttc21b/Ift139, shows signs of excessive Shh signaling (Tran et al., 2008). A role for retrograde IFT in Gli3 processing (Huangfu and Anderson, 2005; May et al., 2005) and Gli2 activity might explain the observed overactivity of both Gli2 and Gli3 in aln mice. Finally, in Ftm knockout mice, Gli3 processing is specifically affected, suggesting a role for basal body proteins in Hedgehog signaling, specifically Gli3 processing (Vierkotten et al., 2007).

The availability of conditional ciliary mutants has facilitated the dissection of the role of Shh signaling in a variety of different tissue types and organisms. Hh signaling in skeletogenesis has been evaluated by the conditional ablation of Kif3a in mouse cartilage (Koyama et al., 2007) and the conditional ablation of Kif3a or Ift88 in the developing limb (Haycraft et al., 2007), exposing a unique role of cilia and Ihh signaling in skeletogenesis, although the cartilage phenotype is only partially phenocopied by Ihh ablation (Koyama et al., 2007).

Similarly, targeted disruption of Kif3a in a subset of neural progenitors in mice led to reduced production of new neurons in the dentate gyrus, probably due to a lack of granule neuron precursors (Han et al., 2008). The phenotypic overlap between these mice, Ift88 hypomorphs, and _Ftm_-deficient mice suggests a general requirement for basal body and cilia function in proliferation of granule neuron precursors in the dentate gyrus. In addition, the observed proliferation defects coincided with decreased Shh activity in the developing brain at E18 as judged by both Gli1 and Ptch1 expression. Similar effects were observed in cerebrellar granule cell precursors, extending the role of Shh signaling beyond the dentate gyrus (Spassky et al., 2008). Thus, targeted ablation of primary cilia can identify novel roles for Hh signaling during development and adult tissue homeostasis.

With the role of the primary cilium in Hh signaling firmly established, it remains unclear whether all or only a subset of Hh signaling events are mediated by the primary cilium. The predominance of floor plate specification, neural tube ventralization, and limb patterning defects observed in ciliary mutants over other Hh-associated defects has been striking. The most severe ciliary mutant phenotypes (mice lacking Kif3a or Ift88) manifest in embryonic lethality at or around E10.5, preceding the developmental stages when Shh defects such as cyclopia (E12.5) or hair follicle maturation defects (E14.5) can be observed. Of note, Hh signaling components are highly conserved among Drosophila and mammals, although the pathway is active in nonciliated cells in the flies. It is unclear, however, whether this implicates a ciliary specialization in vertebrates and that the cilium has been co-opted by morphogenetic signaling pathways, or whether the cilium has been lost in the evolution of diptera such as Drosophila melanogaster. A more detailed understanding of the individual pathways in a time- and tissue-specific context will likely lead to a more nuanced view of the role of the primary cilium in Hedgehog signaling.

Other Signaling Pathways

In primary mouse embryonic fibroblasts and NIH 3T3 fibroblasts, platelet-derived growth factor receptor PDGFRαα as well as an activated downstream component (phospho- Mek1/2) localize to the primary cilium during G0 (Schneider et al., 2005). Embryonic fibroblasts of orpk mutant mice are not activated by PDGF-AA stimulation, implying that ciliary localization of PDGFRαα is necessary for proper signal transduction. While this is suggestive of a cilia-specific role for PDGFRα in homeostasis and mitogenic signaling, it has not yet been shown that PDGFRαα signaling regulates cell cycle reentry of quiescent cells in vivo.

G protein-coupled receptors also localize to rodent neuronal cilia, including the serotonin subtype 6 receptor (5-HT6) (Brailov et al., 2000), somatostatin receptor3 (Sstr3) (Handel et al., 1999), and melanin-concentrating hormone receptor1 (Mchr1) (Berbari et al., 2008). The loss of Bbs2 or Bbs4 leads to mislocalization of Sstr3 and Mchr1 in mice (Berbari et al., 2008). The localization of β-arrestin1/2 to the cilium may have implications beyond the Shh signaling pathway, where it mediates complex formation between Smo and Kif3a (Kovacs et al., 2008). This is because β-arrestins are known to play a role in the regulation of seven-transmembrane receptor-mediated signaling (Lefkowitz et al., 2006). Yet, it has not been demonstrated that ciliary localization of the receptors or β-arrestin is a prerequisite for somatostatin- or Mch-mediated signaling or that these signaling pathways are impaired in ciliary mutants.

Consequences of Ciliary Dysfunction

The Ciliopathies: Clinically Distinct but Overlapping Phenotypes

The link between pathological phenotypes and ciliary dysfunction in humans was proposed initially in the 1970s, when Bjorn Afzelius and others noticed that individuals with chronic bronchitis, immotile sperm, and situs inversus had diminished ciliary motility due to the lack of outer dynein arms (Afzelius, 1976). However, it was not until recently when defects in proteins that localize to the basal body and axoneme of nonmotile 9+0 primary cilia were causally related to human disease. With the help of complete genomic sequence information, coupled to both spontaneously mutated and gene-targeted vertebrate animal models, a multitude of human diseases have now been attributed to defects in ciliary and basal body proteins. Collectively, these human syndromes are termed “ciliopathies” (see Badano et al., 2006, and references within), disorders defined by unique clinical criteria, but which present many overlapping phenotypes such as retinal degeneration, polydactyly, situs inversus, mental retardation, encephalocele (due to failure of neural tube closure), and cysts in the kidney, liver, and pancreas. We proposed previously that these common phenotypes could be used as predictors to implicate the genes/proteins involved in disorders of unknown genetic basis in ciliary dysfunction, and a recent report demonstrating that mutations in IFT80 are associated with Jeune Asphyxiating Thoracic Dystrophy (JATD) represents a proof of principle for this idea (Beales et al., 2007).

In the following section, rather than exploring each ciliopathy in detail (for comprehensive reviews, see Badano et al., 2006; Fliegauf et al., 2007), we will highlight cellular and molecular explanations for the phenotypic variation both within and across syndromes.

The Cellular Basis of Pleiotropy

Given that cilia are present in most vertebrate tissues, it is not surprising to observe pleiotropy in ciliary disorders. However, the extent to which patients are affected (expressivity) depends on the spatiotemporal context of the mutated protein. Some ciliopathies, such as autosomal dominant polycystic kidney disease (ADPKD), and the earlier-onset autosomal recessive polycystic kidney disease (ARPKD) are largely confined pathologically to the kidneys, liver, and pancreas. This might be attributed to tissue-specific expression of the mutated gene products, which are membrane-associated proteins that localize to the cilium, such as polycystin-1 (PC1), polycystin-2 (PC2) (ADPKD), and fibrocystin/polyductin (ARPKD). These are thought to mediate the balance between proliferation and differentiation during organogenesis (Nauli et al., 2003; Wang et al., 2004). On the other hand, global basal body and ciliary disorders are caused by compromised protein function in multiple tissues. For example, Bardet-Biedl (BBS), Meckel-Gruber (MKS), and Joubert Syndrome (JBTS) patients all share overlapping phenotypes such as cystic kidneys, central nervous system (CNS) developmental defects, and polydactyly (Badano et al., 2006). Accordingly, all genes that cause these three disorders are necessary for proper function of the basal body and cilium during development in a wide range of tissues (Table S1, available online).

Tissue specificity and temporal expression of ciliary proteins is only one facet adding to our understanding of the complexity of ciliary phenotypes. An additional contributing factor is the observation that some proteins that carry out distinct functions in cilia may localize to two discrete cellular pools, which may either be functionally related or be devoted to unique cellular tasks. PC2 is a notable example of a ciliary protein that carries out dual cellular roles. Nauli and colleagues first proposed that in primary cell cultures of mouse renal cilia, PC2 functions in conjunction with PC1 as an ion channel required for fluid-flow-induced Ca2+ signaling (Nauli et al., 2003). Additionally, a cilia-specific role for PC2 in Ca2+ signaling, albeit independently of PC1, has also been demonstrated in the mouse node; McGrath et al. observed that PC2 localizes to both peripheral and central monocilia in the node at E7.5 and that asymmetric calcium transients correspond to the presence of PC2 (McGrath et al., 2003). However, PC2 has also been shown to function as a Ca2+ channel at the plasma membrane and endoplasmic reticulum (Tsiokas et al., 2007). Intriguingly, cardiovascular abnormalities are a major complication of ADPKD, which may result from dysfunctional PC2-mediated Ca2+ signaling at the sarcoplasmic membrane of smooth muscle cells (Qian et al., 2003). This represents a potential ciliary-independent phenotype of ADPKD, although the paucity of information about ciliary function in muscle cells does not merit exclusion of a possible ciliary role for PC2 in the cardiovascular system.

Inversin is another protein contributing to renal pathologies that may be conducting multiple roles within the cell. We know from the inv mouse model that inversin plays a role in both the node in the establishment of left-right asymmetry (reviewed by Hirokawa et al., 2006), and also in the promotion of renal development and homeostasis. Reports of inversin localization to the intercellular cell membrane (Nurnberger et al., 2002), coupled with data demonstrating that inversin is expressed as early as the two-cell stage in mouse embryos, presents the possibility that inversin may function prior to the appearance of the node to contribute in a yet unknown way to establish left-right asymmetry (Eley et al., 2004). Studies in Xenopus embryos have demonstrated that left-right asymmetry may be established before the development of Spemann’s Organizer (the mouse node equivalent) with differential cell membrane potentials governed by H+/K+ ATPase expression (Levin et al., 2002). Therefore, we cannot exclude the possibility that inversin functions similarly in a nonciliary role to break left-right asymmetry.

The cilia-independent role of KIF3A in establishing polarity in neurons has complicated the assessment of the true ciliary phenotype in null models. Abrogation of Kif3a in mice pheno-copies other IFT complex mutants; they are embryonic lethal and display laterality defects resulting from the absence of cilia at the node (Marszalek et al., 1999). However, KIF3A was recently reported to function as a KIF3B-independent molecular motor that interacts with the PAR3/PAR6/aPKCζ complex to establish neuron polarity. Two independent reports showed that KIF3A is the molecular motor required to transport PAR3 to the tip of developing hippocampal neurites to specify the neuronal axon and, consequently, neuronal polarity (Nishimura et al., 2004; Shi et al., 2004). As a preliminary attempt to explore the central nervous system in ciliary mutants, Kif3a was conditionally targeted in the mouse cerebellum and the observed abnormal development was attributed in part to defects in granule cell proliferation (Chizhikov et al., 2007). However, it remains to be elucidated whether altered neuronal polarity might contribute to the phenotype in these mutants.

In contrast to PC2, inversin, and KIF3A, which carry out similar functions in different cellular compartments, IFT57/Hippi (huntingtin interacting protein-1 protein interactor) performs two entirely different roles in the cell. IFT57 is an IFT complex B protein, and mice lacking Hippi display laterality defects and aberrant Shh downregulation consistent with the absence of cilia (Houde et al., 2006). However, Hippi has been documented previously as a contributor to the neuronal apoptosis observed in Huntington’s disease (Gervais et al., 2002). These observations challenge the notion that some of the neuronal degenerative phenotypes that we observe in ciliopathy patients are due exclusively to ciliary function, particularly if IFT57 is responsible for any of the pathogenic or modifying alleles that we observe in ciliary syndromes.

Allelic Variants: Same Gene, Differing Severity

In agreement with the substantial number of proteins that are required for correct function of the basal body and cilium in vertebrates, we know that ciliopathies are not only pleiotropic in the phenotypes they present, but they are also oligogenic, reflecting the importance of each component of protein complexes that are functioning at the basal body and cilium (Table S1). Importantly, there are now several reports suggesting that pathogenic mutations in one particular gene can contribute to clinically distinct ciliary disorders as allelic variants manifested along a phenotypic spectrum of severity.

On the basis of the phenotypic overlap between MKS, JBTS, BBS, and nephronophthisis (NPHP), several groups have been prompted to examine causative genes across different ciliopathy cohorts. For example, variants in BBS2, BBS4, and BBS6 have been identified in MKS or MKS-like fetuses (Karmous-Benailly et al., 2005). MKS3 mutations have been associated with JBTS (Baala et al., 2007b), and mutations in RPGRIP1L have been reported in MKS, JBTS, and NPHP patients (Arts et al., 2007; Delous et al., 2007; Wolf et al., 2007) (Table S1). Two recent reports have provided functional data indicating that phenotypic severity among ciliopathies is a function of mutational load. Our group identified new sequence variants in MKS-associated genes MKS1, MKS3, and CEP290 in our BBS cohort. Based on an in vivo zebrafish assay to assess the pathogenicity of the missense variants, hypomorphic alleles in MKS1 and MKS3 can contribute pathogenic alleles to the BBS phenotype (Leitch et al., 2008). Similarly, Bergmann and colleagues used ciliopathy patients and mouse models to demonstrate a phenotypic continuum between NPHP- and MKS-like phenotypes. In addition to their previous findings that NPHP3 mutations can cause the renal cystic phenotype of NPHP, they now report pathogenic NPHP3 mutations in fetuses with MKS-like phenotypes. They then modeled the pathogenic significance of these mutations by comparing the phenotypes of the pcy mouse, which harbors a hypomorphic mutation in Nphp3, with a mouse possessing a targeted null Nphp3 allele (Bergmann et al., 2008). Taken together, these studies provide evidence in favor of the ciliopathies as an organellar disorder, rather than multiple distinct clinical entities, the phenotype being a function (or a consequence) of total mutational load in ciliary protein-encoding genes.

The CEP290 gene product, a centrosomal protein expressed in renal epithelial cells and retinal photoreceptors, has emerged recently as a panciliopathy gene. Hypomorphic alleles in CEP290 represent the largest single contributor of mutations to Leber congenital amaurosis (LCA) patients, and a variant conferring only partial protein function is the underlying cause of the retinal phenotype in the rd16 mouse (Chang et al., 2006; den Hollander et al., 2006). CEP290 variants of largely uncharacterized pathogenic potential have also been associated with NPHP, JBTS, and BBS (Leitch et al., 2008; Sayer et al., 2006; Valente et al., 2006). Finally, on the severe end of the phenotypic spectrum, presumably null mutations introducing nonsense or frame-shifting mutations in the extreme N terminus of CEP290 have been reported in MKS fetuses (Baala et al., 2007a). Combined, these reports provide further evidence of allelic variation that is contributing to the phenotypic range among ciliopathies.

Emergence of Previously Unrecognized Ciliary Phenotypes

One of the challenges to ciliary disease is the difficulty in making an accurate patient diagnosis, considering the interplay of multiple genes, alleles, and phenotypes. Renal cystic disease coupled to polydactyly, vision loss, and/or central nervous system defects represent some classical hallmarks of ciliopathies when present in tandem. Two subtle pathogenic phenotypes have been reported recently that expand our understanding of ciliary function in particular cell types and will potentially contribute to the predictive and diagnostic power of ciliary phenotypes.

Vertebrate odorant sensation is mediated by the sensory cilia that decorate the olfactory sensory neurons. Through a still incompletely understood process, odorants bind to G-coupled receptors, and G proteins subsequently facilitate signal transduction in olfactory neurons (Buck and Axel, 1991). BBS patients, as well as mouse mutants lacking Bbs1 or Bbs4, manifest anosmia with concomitant organizational defects of the ciliated layer of the olfactory epithelium and disorganized microtubular structures in apical dendrites (Kulaga et al., 2004). Recently, this phenotype has been also observed in the rd16 mouse with partial loss of function of CEP290; electro-olfactograms indicated that the mice were anosmic, probably because of the mislocalization of olfactory G proteins in the absence of CEP290 (McEwen et al., 2007).

Basal body proteins have also recently been shown to be critical for proper function of the peripheral nervous system and compromised function results in defective thermo- and mechanosensation. BBS proteins localize to the basal bodies of ciliated dorsal root ganglion neurons in normal mice; however, _Bbs_-deficient mice, as well as BBS patients, do not respond to the same temperature and mechanical stimulus range as their wild-type counterparts. In the absence of a gross ciliary structural explanation for these sensory phenotypes, the mislocalization of the STOM3 and TRPV channel proteins in _Bbs-_deficient dorsal root ganglion neurons provides preliminary functional clues of the cellular basis of the phenotype (Tan et al., 2007). Further study of dorsal root ganglion development and support cells such as keratinocytes and glial cells will enable the dissection of this complex phenotype.

Integrating Ciliary Biology and Human Ciliopathies

The unifying organellar basis of the ciliopathies, informed by the dissection of cellular biology in vitro and in vivo, provides unique opportunities in understanding human disease. First, the phenotypic overlap shared across ciliopathies, particularly pleiotropic disorders, holds potential predictive power for syndromes for which the genetic and functional basis are still unknown. For example, postaxial polydactyly in ciliopathy patients is attributable likely to defects in Shh signal transduction, not only evidenced by the ciliary mutant phenotypes, but also by the observed phenocopy of humans with GLI3 mutations (Hill et al., 2007). Further, anosmia in BBS and LCA patients is probably due to defective cellular transport of signaling proteins and/or receptors in ciliated olfactory epithelia. Still, care must be taken in the interpretation of ciliary phenotypes in humans; multiple cellular abnormalities have the potential to manifest similar phenotypes such as the developmental defects in the central nervous system resulting from both Wnt and Shh signal disruption. As our understanding of ciliary function increases in different tissue types, we anticipate that new phenotypes, which may be used for diagnostic purposes, will become apparent.

The concept of a unified collection of disorders with a ciliary basis holds much potential for disease gene discovery. The ciliary proteome predicts that pathogenic variants in as many as 1000 different genes may contribute to the total mutational load of the ciliopathies (Gherman et al., 2006), with many of them having functions that are still unknown. The increased use of ultra-high throughput sequencing technologies and the development of physiologically relevant functional assays should enhance our rate of assignment to total mutational load in patients. We predict that this information will promote a shift from a clinical to a molecular diagnosis in which a collection of a few hypomorphic alleles result in mild phenotypes, and null alleles result in lethal phenotypes.

Concluding Remarks

The vertebrate cilium is a sensory organelle critical for a broad array of homeostatic mechanisms and paracrine signals. Notably, ciliopathy phenotypes manifest as both developmental structural defects and failure of left-right axis determination in a host of clinical disorders, as well as progressive degenerative phenotypes, suggesting that ciliary proteins serve important functions in organogenesis, tissue maintenance, and, potentially, regeneration. The field faces numerous challenges for the future, which include three major questions.

First, what are the similarities and differences (both structural and functional) between primary cilia in different cell types? Given the association of major developmental process with ciliary dysfunction, it is perhaps paradoxical that ciliopathies do not manifest more severe clinical phenotypes. In addition to the usual suspicions of differential tolerance for damage and regenerative ability, it is likely that not all cilia partake in the same signaling processes. To that end, the progress made toward characterizing the complete ciliary proteome must now be refocused toward understanding the protein complement of cilia in particular tissues and cell types.

Second, it is equally important to differentiate between the ciliary and nonciliary roles of these proteins. There is a pervasive ciliocentric view in the current literature—that a protein localizes to basal bodies and cilia in cultured cells and tissues can no longer serve as definitive evidence that a protein’s function is exclusively at the cilium. Several ciliary proteins are now known to serve multiple cellular functions, and it is likely that pools of ciliary proteins will be found in other compartments under specific physiological conditions. Therefore, the burden of proof for a ciliary phenotype in any model system will require multiple independent lines of evidence, including studies of ciliation and deciliation.

Third, the association of the primary cilium with Hedgehog and Wnt signaling opens up several areas of investigation. Most pressing is to identify other pathways in which the primary cilium might play a role. Intriguingly, if basal body integrity is indeed required for proteasomal targeting of a subset of signaling proteins, including, but not limited to, β-catenin (Gerdes et al., 2007), we might expect pathways that require proteasomal processing to be modulated by the cilium. It is unlikely to be coincidental that both Hedgehog (Gli processing) and Wnt signaling (β-catenin degradation) rely heavily on proteasomal processing, and that disruption of both the basal body and cilium result in impaired proteasomal processing of Gli2/3 (Caspary et al., 2007; Delous et al., 2007; Haycraft et al., 2005; Huangfu and Anderson, 2005; Karmous-Benailly et al., 2005) and impaired degradation of Dvl and β-catenin (Gerdes et al., 2007; Simons et al., 2005).

Finally, the near-ubiquitous presence of ciliated structures in vertebrates potentially contains some important evolutionary lessons. In invertebrates, such as Drosophila, only sensory neurons and sperm are ciliated, whereas in vertebrates, nearly every tissue type has cells that are ciliated at some point in their life cycle. We suggest that the role of the cilium in paracrine signaling might have been the direct outcome of the widespread presence of cilia in vertebrates. Clearly, though conserved throughout evolution, signal transduction pathways have diverged from invertebrate to vertebrate organisms. In Drosophila, the Hedgehog and PCP signaling pathways are organized differently than they are in mice and humans. However, it is unclear which fraction of a specific signaling pathway is regulated by the primary cilium, though such regulation is likely to be time and tissue specific.

Supplementary Material

Suppl. Data

Acknowledgments

We are indebted to J. Badano, E. Oh, J. Robinson, and N. Zaghloul for their critical review of the manuscript and A. Gherman for technical assistance. This work was supported by grant R01HD04260 from the National Institute of Child Health and Development (N.K.), R01DK072301, and R01DK075972 (N.K.) and NRSA fellowship F32 DK079541 (E.E.D.) from the National Institute of Diabetes, Digestive and Kidney Disorders, the Macular Vision Research Foundation (N.K.), and the Foundation for Fighting Blindness (N.K.).

Footnotes

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